Method for modulating a bacterial invasion switch

ABSTRACT

The subject matter disclosed herein pertains to the modulation of a bacterial invasion switch and the subsequent use of the bacterium to vaccinate an organism. In one embodiment, the bacterial invasion switch is modulated by changing the proteolysis of ExoR protein. In another embodiment, a mutated bacterium produces a mutant ExoR protein that resists proteolysis.

CROSS-REFERENCE TO RELATED APPLICATIONS

This application claims priority to and is a continuation-in-part of U.S. patent application Ser. No. 13/903,289 (filed May 28, 2013) which is a non-provisional of U.S. Patent Application Ser. No. 61/652,120 (filed May 25, 2012), the entirety of which are incorporated by reference.

STATEMENT OF FEDERALLY SPONSORED RESEARCH OR DEVELOPMENT

This invention was made with Government support under Contract SGM081147 awarded by the National Institute of Health (NIH). The government has certain rights in the invention.

BACKGROUND OF THE INVENTION

The subject matter disclosed herein relates to a method of modulating a bacterial invasion switch and the subsequent use of the treated bacterium to vaccinate an organism.

BRIEF DESCRIPTION OF THE INVENTION

In one embodiment, the disclosure pertains to a method for modulating a bacterial invasion switch by changing the proteolysis of ExoR protein. The method comprises a step of administering a protease inhibitor to a bacterium which changes proteolysis of ExoR to modulate an invasion switch of the bacterium, thereby keeping the bacterium in a non-pathogenic state. A first ExoR level is determined after the step of administering wherein the first ExoR level is lower than a second ExoR level prior to the step of administering.

In another embodiment, the disclosure pertains to a method for immunizing an organism by introducing a mutated bacterium to the organism. The bacterium has a bacterial invasion switch that has been modulated by changing the proteolysis of ExoR protein. The method comprises making a mutant bacterium wherein the mutant bacterium produces a mutated ExoR_(m) protein that is resistant to proteolysis relative to a wild-type bacterium thereby placing the bacterium in a non-pathogenic state. The mutant bacterium is introduced to an organism and the organism is permitted an opportunity to produce an immune response to the mutant bacterium.

An advantage that may be realized in the practice of some disclosed embodiments of the method is that the organism has the opportunity to produce an immune response to a whole body bacterium.

This brief description of the invention is intended only to provide a brief overview of subject matter disclosed herein according to one or more illustrative embodiments, and does not serve as a guide to interpreting the claims or to define or limit the scope of the invention, which is defined only by the appended claims. This brief description is provided to introduce an illustrative selection of concepts in a simplified form that are further described below in the detailed description. This brief description is not intended to identify key features or essential features of the claimed subject matter, nor is it intended to be used as an aid in determining the scope of the claimed subject matter. The claimed subject matter is not limited to implementations that solve any or all disadvantages noted in the background.

BRIEF DESCRIPTION OF THE DRAWINGS

So that the manner in which the features of the invention can be understood, a detailed description of the invention may be had by reference to certain embodiments, some of which are illustrated in the accompanying drawings. It is to be noted, however, that the drawings illustrate only certain embodiments of this invention and are therefore not to be considered limiting of its scope, for the scope of the invention encompasses other equally effective embodiments. The drawings are not necessarily to scale, emphasis generally being placed upon illustrating the features of certain embodiments of the invention. In the drawings, like numerals are used to indicate like parts throughout the various views. Thus, for further understanding of the invention, reference can be made to the following detailed description, read in connection with the drawings in which:

FIG. 1 is a depiction of a signal sensing pathway for a bacteria utilizing three proteins: ExoR, ExoS and ChvI;

FIG. 2 is a flow diagram depicting an exemplary method for modulating a bacterial invasion switch by changing the proteolysis of ExoR protein;

FIG. 3 is a flow diagram depicting an exemplary method for immunizing an organism by introducing a mutated bacterium to the organism;

FIG. 4 is a schematic representation of the ExoR protein showing signal peptide (SP), four putative Sell protein-protein interaction domains (SEL1), a FLAG-tagged ExoR protein (ExoR-CF), two mutated ExoR proteins (ExoR95 and ExoR108), the proteolysis region of ExoR, the amino acids that are conserved (in black-shaded letters) around the proteolysis region, and the positions of the three amino acids that were mutated to alanine (A) for functional analyses;

FIG. 5 is a Western blot showing ExoR protein profiles of the S. meliloti wild-type Rm1021, exoR95 mutant, exoR108chvI109 double mutant, and the double mutant exoR108chvI109 (pHC510), which is labeled as pexoR mutant expressing the wild-type exoR gene;

FIGS. 6A, 6B and 6C are a functional analyses of the wild-type ExoR protein and C-terminal FLAG-tagged ExoR proteins with each protein expressed in the exoR95 background and in the exoR108chvI109 double mutant background to determine its function in regulating succinoglycan production, as determined by the levels of colony brightness on calcofluor-containing medium (6A), and flagellum production as determined by the size of swimming colonies (6B) and the functions of these modified ExoR proteins in nodulation were measured according to the percentage of pink nodules (6C) in the exoR95 mutant background wherein the plasmids for the expression vector, pexoR and pexoR-cf are pMB393, pHC510, and pHC630, respectively;

FIGS. 7A, 7B and 7C show the cellular location of ExoR protein and site of proteolysis. Schematic representation of three different ExoR-PhoA fusions (7A) and their corresponding phosphatase activities in the S. meliloti Rm8002 background (7B). Boxes with vertical stripes represent ExoR signal peptide. ExoR protein profiles were determined by western blot (7C) for wild-type ExoR protein expressed from pHC518 (pR) and the ExoR protein without signal peptide, ExoR_(m), expressed from plasmid pHC641(pR_(m)) in the exoR95 mutant background;

FIGS. 8A and 8B are Western blot protein profiles of the exoR95 mutant carrying plasmid pHC510 and pHC630 expressing wild-type ExoR and ExoR-CF, respectively. Proteins were immunoprecipitated (IP) with FLAG antibody, and detected with either ExoR polyclonal antibodies (8A) or FLAG antibody (8B);

FIG. 9 shows amino acid sequence alignment of ExoR proteolysis regions from 16 ExoR orthologs. Conserved amino acids are shaded. The overall amino acid identities between S. meliloti ExoR and its orthologs are listed. The positions of the amino acids and the site of proteolysis are marked based on S. meliloti ExoR protein. The following species are shown: S. m. (S. meliloti Rm1021), S.m.w. (Sinorhizobium medicae WSM419), R. sp. (Rhizobium sp. NGR234), A. v. (Agrobacterium vitis S4), A. t. (Agrobacterium tumefaciens str. C58), A. r. (Agrobacterium radiobacter K84), R. 1. (Rhizobium leguminosarum bv. trifolii WSM2304), Hp. (Heoflea phototropica DFL-43), R. e. (Rhizobium etli CIAT652), M sp. (Mesorhizobium sp. BNC1), 0.1. (Ochrobactrum intermedium LMG 3301), 0. a. (Ochrobactrum anthropi ATCC 49188). B. a. (Brucella abortus str. 2308 A), B. c. (Brucella ceti str. Cudo), B. o. (Brucella ovis ATCC 25840), and B. m. (Brucella melitensis 16M);

FIGS. 10A, 10B, 10C and 10D are a biochemical and functional analysis of ExoR proteolysis product ExoR_(c20), which was expressed from pHC510 (pR) and pHC567 (pSP-Rc20) in the exoR108chvI109 mutant for ExoR and SP-ExoR, and probed in western blot (10A). The effects the presence of ExoR_(c20) on succinoglycan production was measured by calcofluor fluorescence (10B and 10C) and its effects on swimming ability was measured by the size of the colonies (10D);

FIGS. 11A, 11B, 11C and 11D are a biochemical and functional analysis of ExoR proteins with single amino acid mutations, ExoRL81A, ExoRW79A, and ExoRY87A, expressed from plasmids pHC571, pHC572, and pHC573, respectively, in the exoR108chvI109 mutant for western blot (A), and in the exoR95 mutant for their effects on succinoglycan production (B and C) and swimming ability (D); and

FIG. 12 is a model of the ExoR-ExoS/ChvI signal-transduction pathway. It is hypothesized that the active mature form of ExoR, ExoR_(m) is digested via slow proteolysis in wild-type cells. An increase in ExoR proteolysis triggered by environmental or plant signals or mutations in the exoR genes will reduce the amount of ExoR_(m) binding to the ExoS sensing domain, leading to the activation of ExoS sensor and the activation or suppression of expression of the genes regulated by the ExoS/ChvI two-component regulatory system.

DETAILED DESCRIPTION OF THE INVENTION

To conserve biological energy, bacteria maintain one of two states: a free-living (non-pathogenic) state or an infective (pathogenic) state. Each of these states are characterized by certain genes being activated or deactivated. Generally, when a bacteria is in an environment that is less suitable for replication (e.g. on a non-living or infection resistant surface) the bacteria in the free-living state. When the bacteria is in an environment that is more suitable for replication (e.g. within a host organism) the bacteria changes to the infective state. A signaling mechanism must be present that permits the bacteria to sense its environment and selectively enter one of these states, however, the nature of this signaling mechanism is not known. Disclosed in this specification are details of such a signaling mechanism and a method that utilizes this newly discovered mechanism to maintain a bacteria in a free-living (non-pathogenic) state.

FIG. 1 is a depiction of a signal sensing pathway for a bacteria utilizing three proteins: ExoR, ExoS and ChvI. Without wishing to be bound to any particular theory, ChvI is thought to form a signal pathway with ExoS. ExoS, in turn, forms a complex with ExoR. To the extent the ExoS/ExoR complex is predominant, the free-living (non-pathogenic) state is favored. Conversely, reduction in the level of ExoS/ExoR complex produces a corresponding increase in the level of infective (pathogenic) bacteria. The degree to which the ExoS/ExoR complex is formed is controlled, at least in part, by the concentration of free ExoR. ExoR has been found to exist in two states: an ExoR_(p) (precursor, 29 kD) that is found in the cytoplasm and ExoR_(m) (mature, 26 kD) that is found in the periplasmic space between the inner and outer membranes. It is believed ExoR_(m) is the form of the protein that binds with ExoS in the periplasmic space to maintain the bacteria in a free-living (non-pathogenic) state. It is further believed there is an equilibrium between the bound ExoS/ExoR_(m) complex and the free ExoR_(m) state and that this equilibrium is the signaling mechanism that switches the bacteria between free-living and infectious states. Specifically, the ExoR_(m) (26 kD) is subjected to proteolysis to yield a 6 kD fragment and an ExoR_(c20)(20 kD) fragment. This proteolysis shifts the equilibrium toward the free ExoR_(m) state which reduces the ExoS/ExoR complex and thereby favors the infectious state. Environmental factors, including high salt concentration, have been found to facilitate the proteolysis of ExoR_(m). This explains why, upon exposure to the relatively high-salt environment of a host, the bacteria are rendered pathogenic.

In one embodiment, a method is provided for inhibiting the proteolysis of ExoR_(m). Such a method disrupts the bacteria's ability to disassociate the ExoS/ExoR complex and thereby locks the bacteria into a free-living (non-pathogenic) state. For example, a protease inhibitor may be used to reduce or halt the proteolysis of ExoR_(m). In another example, a bacteria is produced with a mutated exoR gene which, in turn, produces an ExoR_(m) variant that is resistant to proteolysis. Such a bacteria may be introduced into a host so as to permit the host the opportunity to produce an immune response without risking the bacteria becoming pathogenic. This provides an alternative mechanism to vaccinate the host. One such exemplary method is depicted in FIG. 2.

FIG. 2 is a flow diagram depicting an exemplary method 200 for modulating a bacterial invasion switch by changing the proteolysis of ExoR protein. In some embodiments, the method 200 comprises a step 202 of exposing a bacterium to a cell penetration agent. In one embodiment, the cell penetration agent is a detergent known to increase the permeability of cellular membranes. In one such embodiment, the detergent is sodium dodecyl sulfate (SDS). In another embodiment, the cell penetration agent is a cell-penetrating peptide.

The method 200 further comprises a step 204 of administering a protease inhibitor to the bacterium which changes proteolysis of ExoR to modulate an invasion switch of the bacterium. This lack of proteolysis has the effect of keeping the bacterium in a non-pathogenic state. Specifically, the ExoR form that is changed or prevented from undergoing proteolysis is the mature form, ExoR_(m). In one embodiment, the protease inhibitor is phenylmethylsulfonyl fluoride (PMSF). In one embodiment, the protease inhibitor is selected to permeate a cellular membrane such that it resides in the periplasmic space between two adjacent membranes. For example, the protease inhibitor may be a non-protein molecule with a molecular weight of less than about three hundred grams per mole. Additional examples of such protease inhibitors are known in the art.

To digest specific substrates, enzymes bind to their substrates through strict structure matching. This strict structure matching creates the opportunity to inhibit enzymatic activities through direct and indirect approaches.

Direct Inhibitors of Enzymatic Reactions

Direct Inhibitors resemble the enzyme substrates and compete with the substrate to occupy the active site of the enzyme, preventing the interaction of enzyme and substrate, which leads to the inhibition of enzymatic reaction.

The direct inhibition involves using an inhibitor, which is a carrier molecule linked to a substrate mimicking molecule. The substrate mimicking molecule has the same shape and physical characteristics of the part of substrate, epitope, that binds to the active binding site of an enzyme. The known direct inhibitor, PMSF (phenylmethanesulfonylfluoride), that fits securely into the ExoR_(m) protease, covalently links to the serine in the active site of the protease, preventing the ExoR_(m) protease from binding and digesting ExoR_(m). PMSF, for example, has the mimicking molecule F-SO₂ and carrier molecule phenyl ring, which serves to stabilize and present the mimicking molecule F-SO₂. The carrier molecule, phenyl ring, could be any types of biomolecule, which includes nucleic acid(s), amino acid(s), or lipids. The function of this molecule is to maintain the structure of the inhibitor so that the epitope is on the surface at the right angle to fit into active binding site of ExoR_(m) protease. An elongated narrow structure will further enhance the ability of the direct inhibitors to reach the periplasm of Sinorhizobium meliloti cells to interact with the ExoRm protease.

Examples of small molecule that function as direct inhibitors include PMSF, AEBSF (4-(2-Aminoethyl)benzenesulfonyl fluoride hydrochloride), Camostat, and Methoxy arachidonyl fluorophosphonate. In one example, the inhibitor has a structure consistent with FSO₂—CH₂—C₆H_(a)—R1-R6 as shown below.

R2 to R6 each represent H or (CH₂)—CH₃ or X; or (CH₂)_(n)NH₂; n: number of CH₂; X represents a large carbohydrate moiety, which could comprised of multiple rings. O: oxygen, one of them (R2-R6) can be replaced by other molecules; F: fluoride, can be replaced with other molecules that could support the reactive oxygen; S: sulfur, which can be replaced with other molecules that could support the reactive oxygen;

In one embodiment, the protease inhibitor has a structure consistent with FSO₂—CH₂R, where R is selected from the group consisting of an arene, a nucleic acid, an amino acid and a lipid. Examples of suitable arenes include C₆H₅; o-C₆H₄CH₃; m-C₆H₄CH₃; p-C₆H₄CH₃. Examples of suitable nucleic acids include adenine, cytosine, guanine, thymine, uracil and combinations thereof. In one embodiment, the nucleic acid is a polynucleic acid comprising more than one, but fewer than one hundred, nucleic acids. In another embodiment, more than one, but fewer than six nucleic acids are present. In another embodiment, the nucleic acid is a mononucleic acid. Examples of suitable amino acids include positively charged amino acids (arginine, histidine, lysine); negatively charged amino acids (aspartic acid, glutamic acid); polar amino acids (serine, threonine, asparagnine, glutamine), hydrophobic amino acids (alanine, isoleucine, leucine, methionine, phenylalanine, tryptophan, tyrosine, valine) as well as cysteine, glycine, proline and selenocysteine. In one embodiment, the amino acid is a polypeptide comprising more than one, but fewer than one hundred, amino acids. In another embodiment, more than one, but fewer than six amino acids are present. In another embodiment, the amino acid is a single amino acid. Examples of protein or large molecule as inhibitor include: serpin (family of inhibitors), alpha-1 antitrypsin, alpha-2 antiplasmin, antithrombin, Cl-inhibitor, conspin, CU-2010, CU-2020, Maspin, Protein C inhibitor, Protein Z-related protease inhibitor.

Indirect Inhibitors of Enzymatic Reactions

Indirect inhibitors block the binding of an enzyme with its substrate but they rely on changing the structure of either substrate or enzyme, or changing the structure of both substrate and enzyme. Such structural changes prevent the binding of enzyme and substrate thus inhibiting the activities of the enzymes. Indirect inhibitors include any chemical and physiological conditions that can induce protein structural changes. This includes ionic strength, pH, osmotic pressure, temperature and many others, in addition to specific chemicals. Two examples of indirect inhibitors of ExoR_(m) protease are described below.

Examples 1: at low pH, majority of ExoR_(m) is turned into monomeric form due to increased surface charges and digested by protease, results in the absence of ExoR_(m). In neutral pH, about 50% of ExoR_(m) is in the dimer form and 50% in the monomer form, which is the form that has the epitope exposed and sensitive to protease binding and digestion. When pH of the buffer is increased, the charge on the surface of the substrate, ExoR_(m), is reduced, the ExoR_(m) protein is increasingly attract to each other, producing more of the dimer form, which is resistant to protease digestion. Accordingly, substrates that can chelate proton to increase pH are indirect inhibitors of ExoR_(m).

Lowering pH, on the other hand, increases surface charges of ExoR_(m) and turning ExoR_(m) into monomeric form and sensitive for protease digestion. Low pH will create a condition to screen for direct inhibitor of ExoR_(m) protease. S. meliloti cells changes from free-living swimming cells to non-swimming host invading cells. Under this condition, a direct inhibitor will make the most difference in competing and inhibiting ExoR_(m) protease. Potential inhibitors can be mixed with S. meliloti cells to form swimming colonies at low pH and would be direct inhibitors.

By way of illustration, and not limitation, a low pH may be between about 2 and about 6.9 and a high pH may be above 6.9. In one such embodiment, the high pH is between 6.9 and 8.0 such that ExoR_(m) digestion is slowed and ExoR_(m) accumulates and the RSI invasion switch is shut down thereby turning the bacterium into a free-living state. The changing of pH from pH 2-6.9 to 7.0-8.0 can be achieved by neutralizing using alkaline solution, or substrates that can chelate proton. In other embodiments, the high pH is between 8.0 and 9.0. In still other embodiment, the high pH is above 8.0.

Example 2. In no calcium or low calcium condition, most of ExoR_(m) is in the monomeric form sensitive to protease digestion. Adding 1 mM or more Ca will turn ExoR_(m) into dimeric form, preventing protease from binding and digesting ExoR_(m). So Ca is an indirect inhibitor of the protease. Experiments have shown 1 mM Ca can turn protease active, non-swimming S. meliloti cells into swimming cells regardless of protease activity. This is a typical indirect inhibitor. In the same fashion, most ions are indirect inhibitors of ExoRm protease.

Low ion concentrations, on the other hand, create an environment where protease is most active because more ExoR_(m) is in the monomeric form. Low ion concentration can be created by either including low ions in media, or adding metal chelator, such as calcium chelator EGTA, or sodium chelator EDTA. These conditions can be used to screen direct inhibitors most effectively.

In one embodiment, the protease inhibitor is a metal cation. Examples of suitable metal cations include sodium, calcium, potassium, phosphate, iron. The metal ion may be present in a concentration above the concentration found naturally in soil or fresh water. For example, natural calcium concentration in soil is about 1 mM and sodium is less than 5 mM. The concentration will function as protease inhibitor may be at least 2 mM calcium or at least 150 mM sodium.

Screening for Inhibitors

Many strategies to screen for direct and indirect inhibitors of ExoR protease can be developed using the disclosed understanding of conditions that increase or decrease protease activities. Here are two examples

Example 1. Whole cell motility assay: The whole cell motility assay is based on the fact that inhibition of the protease lead to ExoR_(m) increase and the cell becoming motile. The initial condition may be set with either low pH or low ion concentration, so that S. meliloti cells will form non-swimming colonies. The putative direct or indirect inhibitors can be mixed with S. meliloti cells in soft agar plates. The ones that can make S. meliloti cells to form swimming colonies are the potential direct or indirect inhibitors.

Example 2. fluorescence reporter assay: One of the ways to further confirm the putative inhibitor is inhibiting protease activities is to examine its effects on the expression of the genes regulated by the ExoR_(m) protein. Under normal growth condition, neutral pH and modest ion concentration (1 mM Ca for example), 50% of the ExoR_(m) is in dimer form, the expression of the exo genes for succinoglycan biosynthesis, is kept at low level, while the expression of the fla genes for flagellum biosynthesis is kept at high level. This is a reflection of the activities at a normal level. The green fluorescence protein, GFP, is fused to either the promoter of fla and exo genes. The plasmids carrying these fusions will be conjugated into S. meliloti cells with help plasmid. A true ExoR protease inhibitor will cause S. meliloti cells carrying fla-gfp fusion to turn green under fluorescent light. This because inhibition of protease directly or indirectly will increase the ExoR_(m) level and then the levels of fla gene expression.

Example 3 protease activity assay: The activities of ExoR protease can be measured directly in an in vitro assay using purified ExoR_(m) protein and purified protease. The ExoRm protein can be tagged with His and/or SUMO tags and purified with nickel column. The ExoR_(m) protease is located in periplasm, which can be isolated through fractionation. When ExoR_(m) protein is mixed with ExoR_(m) protease in natural conditions, neutral pH and modest ionic concentration, 50% of the ExoR_(m) protein will be digested to yield a 20 KDa digestion production, ExoR_(c20). When this reaction mixture is resolved on SDS-PAGE gel, the ratio of ExoR_(m) vs ExoR_(c20) can be easily determined. The chemical that can prevent the formation of the ExoR_(c20) is an ExoR protease inhibitor. The products can be further analyzed to determine whether they are direct inhibitors or indirect inhibitors by mixing with ExoR_(m) protein without the protease. The chemical that increase the percentage of ExoR_(m) into dimeric form are indirect inhibitor of ExoR_(m) protease.

The method 200 further comprises a step 206 of determining a first ExoR level after the step of administering wherein the first ExoR level is lower than a second ExoR level prior to the step of administering. Specifically, the ExoR form that is determined is the mature form, ExoR_(m). In one embodiment, step 206 comprises testing the bacterium to verify an ability of the bacterium to invade an organism. If the bacterium's ability to invade is comprised, relative to an untreated bacterium, then the first ExoR levels have been determined to be lowered by method. Such an ability to invade can be determined by conventional techniques including, but not limited to, simple microscopy of a macrophage, detection of an immune response (or other biological response including symbiosis) of the organism.

The method 200 further comprises a step 208 of introducing the bacterium to an organism and, in step 210, permitting the organism an opportunity to produce an immune response. In one embodiment, the organism is an animal. In another embodiment, the organism is a plant. Examples of methods of introduction include oral administration, injection, topical application, and the like. In one embodiment, the step 208 is only performed after step 206 has been completed and the bacterium has been confirmed as being successfully modified. The particular bacterium utilized in step 208 are from the same bacteria sample as the bacterium utilized in step 206. By being introduced to the full bacterium while it is in a non-pathogenic state, the organism has the opportunity to produce antibodies corresponding to the full surface of the bacterium. In contrast, current vaccines are typically made from very few proteins or surface molecules of bacteria, which means only small areas of bacterial cells can be recognized by our immune systems. The disclosed method presents the whole body bacteria to provide a superior immunization method.

FIG. 3 is a flow diagram depicting an exemplary method 300 for immunizing an organism by introducing a mutated bacterium to the organism. The method 300 comprises a step 302 of making a mutant bacterium wherein the mutant bacterium produces a mutated ExoR_(m) protein that is resistant to proteolysis relative to a wild-type bacterium. Such a mutated bacterium is locked in a non-pathogenic state. Methods of making such a mutant are known to those skill in the art. For example, mutations can be induced using polymerase chain reaction (PCR) techniques or by random chemical mutagenesis. Once mutations are induced, the resulting bacteria can be screened to isolate mutated strains of the ExoR protein.

The method 300 further comprises a step 304 of introducing the mutant bacterium to an organism and, in step 306, permitting the organism an opportunity to produce an immune response to the mutant bacterium. The steps 304 and 306 parallel the steps 208 and 210 of method 200.

In one embodiment, the method is used to promote plant growth with increased nitrogen fixing symbiosis. The growth of a plant is limited by the availability of nitrogen. While most plants will stop growing in the absent of adequate nitrogen nutrient, the plants in the legume family, including all the bean and pea producing plants, establish symbiosis with nitrogen fixing bacteria. Changing the structure of the invasion switch component can increase nitrogen fixing symbiosis thus more plant growth and more food production. The method may also be used to expand farming to areas to dry or too salty to grow crop. Changing invasion switch components can raise dry and salt tolerance of during the establishment of nitrogen fixing symbiosis. For example, salts were found to be the signal for the invasion switch by plant symbiont, S. meliloti, plant pathogen Agrobacterium tumefaciens, and animal pathogen Brucella abortus. This group of bacteria have evolved to use salts secreted by hosts including human and animals as the signals to turn into pathogenic bacteria to be more effective in invading hosts.

In another embodiment, the method is used in agriculture including preventing bacterial infection of plants especially the broad host range pathogen Agrobacterium tumefaciens. Blocking the sensing function of RSI invasion switch in this bacterium will prevent it from turning into pathogen and infect crop plants

Studies Pertaining to ExoR Proteolysis

To understand how ExoR suppression of ExoS is relieved which is required for the expression of ExoS/ChvI regulated symbiosis genes, wild-type ExoR and ExoR95 mutant proteins were characterized. In addition to the previously identified precursor and mature forms of ExoR (designated ExoR_(p) and ExoR_(m), respectively), a 20-kD form of ExoR (designated _(ExoRc20)) was detected that is derived from the wild-type ExoR protein but not from the ExoR95 mutant protein. ExoR_(c20) was isolated directly from S. meliloti periplasm to identify its N-terminal amino acids and the site of the proteolysis, which is highly conserved among ExoR homologs. ExoR_(c20) retains the C-terminus of the wild type ExoR. When expressed directly, ExoR_(c20) did not complement the exoR95 mutation, suggesting that ExoR_(c20) does not function directly in the ExoR-ExoS/ChvI regulatory pathway and that ExoR_(m) is the functional form of ExoR. A single amino acid change (ExoRL81A) at the site of ExoR periplasmic proteolysis resulted in the reduction of the amount of ExoR_(m) and the loss of the regulatory function of the ExoR protein. These findings suggest that ExoR_(m) is a target of periplasmic proteolysis and that the amount of ExoR_(m) could be reduced through an effective proteolysis to release its suppression of ExoS. Further details may be found in provisional patent application 61/652,120, the content of which is incorporated by reference.

The Gram-negative soil bacterium Sinorhizobium meliloti establishes a nitrogen-fixing symbiosis with its plant host alfalfa (Medicago sativa) through a set of complex and reciprocal signal exchanges in the absence of fixed nitrogen sources. The formation of an infection thread inside alfalfa root hairs is an essential step in the early stage of this symbiosis that requires the presence of S. meliloti exopolysaccharides, succinoglycan (SG), EPSII, or capsular polysaccharide (KPS). S. meliloti succinoglycan (SG) has been shown to be much more effective than the other two S. meliloti polysaccharides, exopolysaccharide II (EPS II) and capsular polysaccharide (KPS), at eliciting the formation of infection threads. The structure and biosynthetic pathway of succinoglycan have been well documented although its precise role in eliciting the formation of infection threads remains unknown.

Succinoglycan production is inversely co-regulated with flagellum production by a single signal-transduction pathway consisting of the S. meliloti ExoR protein and the ExoS/ChvI two-component regulatory system and the EmmABC system. While the transcription of succinoglycan biosynthesis genes is upregulated by mutations exoR95::Tn5 and exoS96::Tn5, transcription of the flagellum biosynthesis genes is downregulated. This coordinated regulation is consistent with the switch from free-living to invasion-ready cells that is required at this stage of the symbiosis. It also suggests that the ExoR protein and the ExoS/ChvI two-component system play crucial roles in controlling the overall changes needed for S. meliloti cells to switch from free living to symbiosis inside the root nodules.

The S. meliloti exoR gene was initially identified through isolation of the exoR95::Tn5 mutation, which was later identified and sequenced. The exoR gene encodes a 268-amino acid ExoR protein with a conserved signal peptide for exporting the protein to the bacterial periplasm, as confirmed in recent findings. In addition to regulating succinoglycan and flagellum production, ExoR has been shown to be involved in regulating biofilm production and lipopolysaccharide modifications. The ExoR protein has been found to regulate the expression of a large number of gene functions in very different metabolic pathways, suggesting that ExoR plays other important roles. ExoR homologs have been found and characterized in Rhizobium leguminosarum and Agrobacterium tumefaciens, where they also function in regulating polysaccharide, flagellum, and biofilm production. Many additional ExoR homologs have been discovered in recent genome-sequencing efforts, but little is known about their function.

The S. meliloti ExoS and ChvI proteins form a typical bacterial two-component signal-transduction system. The S. meliloti ExoS protein consists of a large periplasmic domain and a cytoplasmic kinase domain, and it has been shown to phosphorylate S. meliloti ChvI directly. Recent analysis of exoS- and chvI-deletion mutants has shown that the ExoS/ChvI system is essential for symbiosis and that these two proteins regulate the expression of a variety of genes involved in carbon metabolism and many other functions. These findings are consistent with the results of a transcriptome analysis of the exoS96 mutant. Collectively, these findings suggest that the ExoS/ChvI system plays an essential role in preparing S. meliloti cells for their transformation from free living to nitrogen-fixing cells inside the root nodules. The importance of the S. meliloti ExoS/ChvI system was further highlighted by the finding that two of its close homologs are essential for host infections in Brucella abortus and A. tumefaciens.

Recent genetic and biochemical data suggest that ExoR, ExoS, and ChvI form a single signal-transduction pathway. The ExoR protein has been localized to the periplasm of S. meliloti cells, and as confirmed by our unpublished data. ExoR has been found to exist in two forms, the 29-kD full-length precursor form (ExoR_(p)) and the 26-kD mature form without its predicted signal peptide (ExoR_(m)) in wild-type S. meliloti cells. Co-immunoprecipitation of ExoR and ExoS suggested that they form protein complexes. Increased expression of the exoS gene also led to accumulation of ExoR_(m), suggesting that ExoS stabilizes ExoR in the ExoR-ExoS complex. The ExoR-ExoS interaction was interrupted by single amino acid changes in either the ExoR protein or the periplasmic domain of ExoS. Taken together, these findings led to a proposed model in which ExoR interacts with ExoS to form a protein complex that keeps the ExoS in the off state, resulting in conditions favoring free living, with higher levels of flagellum production and lower levels of succinoglycan production.

Expanding on this suggested model, our recent data from genetic analyses suggest that ExoR autoregulates its own expression through the ExoS/ChvI two-component system. Loss of functional ExoR protein in the exoR95 mutant leads to upregulation of exoR gene expression, along with that of succinoglycan biosynthetic genes. This upregulation can be suppressed by single amino acid mutations in the ExoS sensing domain, which is consistent with direct ExoR-ExoS interactions. This raises the possibility that ExoR autoregulation through the ExoS/ChvI system is used to modulate the expression of the genes regulated by the ExoS/ChvI system in response to host or environmental signals.

While current model can explain how ExoR turns off the ExoS/ChvI system, it does not explain how the ExoS/ChvI system is turned on during symbiosis in response to environmental or plant signals. Our new findings, presented herein, provide a better understanding of the molecular basis for ExoR protein's ability to turn the ExoS/ChvI two-component regulatory system on and off.

Materials and Methods Strains, Plasmids and Media

The strains, phage and plasmids used in this study are listed in Table 1 of U.S. provisional patent application 61/652,120. Escherichia coli strains were grown in Luria-Bertani (LB) medium at 37° C. and Sinorhizobium meliloti strains were grown in LB medium supplemented with 2.5 mM MgSO₄ and 2.5 mM CaCl2 (LB/MC) at 30° C. LB/MC agar containing 0.02% (w/v) calcofluor white M2R (Blue Brighter 28, Sigma) was buffered to pH 7.4 with 10 mM HEPES (N-2-hydroxyethylpiperazine-N-2-ethanesulfonic acid) and used to examine succinoglycan production on agar media. The following antibiotics were used at the concentrations indicated: ampicillin, 100 μg ml⁻¹; chloramphenicol, 10 μg ml⁻¹; neomycin, 200 μml⁻¹; kanamycin, 25 μg ml⁻¹; spectinomycin, 100 μg ml⁻¹; tetracycline, 10 μml⁻¹, and streptomycin, 500 μg ml⁻¹.

Motility Assay

Bacterial cell motility was examined using swarming plates containing 0.3% agar as described previously with some modifications. Briefly, fresh cell cultures were prepared and diluted to OD600 of 0.1. Then 2 μL of each diluted culture was inoculated into LB/MC soft agar plate and incubated for 2-3 days to determine colony size.

Plant Nodulation Test

Alfalfa nodulation assays were carried out on plates as previously described with slight modifications. A set of eight alfalfa seedlings were planted in a square Petri dish and all plants were grown inside the Petri dishes. Plants were examined after 4 weeks for number of nodules to determine overall symbiotic efficiency.

Expression and Purification of S. Meliloti ExoR-his for Antibody Production

The S. meliloti exoR ORF was obtained by PCR using Rm1021 genomic DNA as the template and two PCR primers: exoRfNdeI-1 exoRrXhoI-1. The PCR product was digested with NdeI and XhoI, and then cloned into pET-16b between restriction sites NdeI and XhoI to generate plasmid pHC615. The His-tagged ExoR protein was purified from BL21DE3 (plysS, pHC615) with 1 mM IPTG (Isopropyl β-D-1-thiogalactopyranoside) induction and using a Ni-NTA purification system under denaturing conditions (Invitrogen). Purification of the His-tagged ExoR protein was confirmed using Coomassie blue-stained SDS-polyacrylamide gels and sent to Pacific Immunology Company (Ramona, Calif.) to raise ExoR-specific polyclonal antibodies in rabbits. The specificity of the ExoR-specific polyclonal antibodies was confirmed by western blot.

Immunoblotting

For immunoblotting, total cellular proteins or purified protein were resolved by SDS-PAGE, transferred to a PVDF (Polyvinylidene fluoride) membrane (Bio-Rad), detected with primary antibodies including ExoR-specific polyclonal antibodies and FLAG-specific monoclonal antibody coupled with alkaline phosphatase (AP) (Novagen), and treated with NBT/BCIP (nitro-blue tetrazolium and 5-bromo-4-chloro-3′-indolyphosphate) (Sigma) to detect AP activities.

Construction of the exoR108chvI109 Double Mutant

The DNA fragment consisting of nucleotide 88 to 433 of the exoR ORF was generated by PCR using S. meliloti Rm1021 genomic DNA as the template and two PCR primers: exoRdfHindIII-2 and exoRdrBsrGI. The PCR product was digested with HindIII and BsrGI, and cloned into suicide plasmid pK19mob2 ΩHMB to produce pHC508. The resulting plasmid was then conjugated into S. meliloti Rm1021 using helper MT616 in a triparental mating and a few conjugants were isolated after 6 days. The interrupted exoR gene was transduced from the conjugants to Rm1021, which yielded only one transductant, the exoR108 mutant. Insertion of the suicide plasmid into the genome was confirmed by PCR and sequencing the site of insertion. The chvI gene was amplified from the genome of the exoR108 transductant using primers chyIf-27 and chvIr759, and sequenced using primers chvIf293 and chvIr419. The exoS gene was similarly amplified from the genome of the exoR108 transductant using primers exoSf-61 and exoSr1918, and sequenced using primers exoSr407, exoSr829, exoSf653, exoSfl098 and exoSr1912. One single mutation was found in the chvI gene but no mutations were found in the exoS gene. The exoR108 transductant was thus designated exoR108chvI109 double mutant. The construct was confirmed by sequencing. The primers used in cloning and sequencing are listed in Table 2 in U.S. provisional patent application 61/652,120 along with all other plasmid constructions described in this paper.

Constructs Expressing ExoR and ExoR without Signal Peptide

The DNA fragment containing the exoR promoter and ORF was generated in a PCR using S. meliloti genomic DNA as the template and primers exoRfHindIII-1 and exoRrXhoI-2, and cloned in between the HindIII and XhoI sites of a medium copy number plasmid pMB393 to generate pHC510. Similarly, the exoR gene was amplified by PCR using primers exoRfNdeI-3 and exoRrXhoI-3, and cloned into pHC93 to generate pHC518, expressing the wild-type ExoR from the lac promoter on the plasmid. The region of the exoR gene without the signal sequence was amplified using primers exoRfNdeI-2 and exoRrXhoI-3, cloned into plasmid pHC93 to generate pHC641, and used to express ExoR_(m), the form of ExoR lacking its signal peptide.

Construction and Analysis of ExoR-PhoA Fusions

A set of three ExoR-PhoA fusions were constructed. To construct the fusion of PhoA with the full-length ExoR, an XbaI/KpnI DNA fragment containing the E. coli phoA gene (lacking its signal sequence) was prepared by PCR using the genomic DNA of the S. meliloti exoF265:: TnphoA mutant as the template and primers phoAfXbaI and phoArKpnI. An XhoI/XbaI DNA fragment containing the complete exoR ORF except the stop codon was obtained by PCR using S. meliloti Rm1021 genomic DNA as the template and two PCR primers: exoRfXhoI and exoRrXbaI. The two DNA fragments were individually treated with either XhoI/XbaI or XbaI/KpnI, and ligated with XhoI- and KpnI treated a low copy number plasmid pSW213 to generate pHC528. To construct the fusion of PhoA and ExoR without signal peptide, the region of the ExoR-PhoA fusion in pHC528 was amplified without the ExoR signal peptide region using two primers, exoRmfXhoI and phoArKpnI, and recloned into the same region of pSW213 to create pHC555. To create the fusion of PhoA with ExoR signal peptide, the coding region of the ExoR signal peptide was amplified in a PCR using pHC528 as the template and primers exoRfXhoI and exoRsp-phoAr. The region for PhoA was amplified using primers exoRsp-phoAf and phoArKpnI. The two fragments were joined together in an overlapping PCR using primers exoRfXhoI and phoArKpnI. The product of this overlapping PCR was cloned into pSW213 to create pHC533. All three fusions were expressed from an inducible lac promoter on the plasmid with 0.8 mM IPTG.

Construction and Analysis of FLAG-Tagged ExoR Proteins

The unique 8-amino acid FLAG tag (available from Sigma and described in provisional patent application 61/652,120) was inserted into the C terminus of the ExoR protein to help track it. To construct the C-terminal-tagged ExoR, ExoR-CF, a DNA fragment containing ExoR and the FLAG tag was generated by PCR using S. meliloti genomic DNA as the template and primers exoRfHindIII-1 and exoRcflagrXhoI, which introduced the FLAG tag. This DNA fragment was cloned into pMB393 to generate pHC630 and express ExoR-CF.

To track FLAG-tagged ExoR proteins, cells of S. meliloti strains expressing ExoR-CF fusion were collected from exponential-phase cultures, washed with CoIP buffer, and resuspended in 3 ml CoIP buffer with 1% (w/v) Triton X-100, 10 mM MgCl₂, 30 mg lysozyme and 30 units of DNAse I at 4° C. for 30 min, and sonicated (550 Sonic Dismembrator, Fisher Scientific) twice on ice (Level 2, 4.5 min each time). Cell lysates were centrifuged at 4° C., 13,000 rpm in a microcentrifuge for 5 min. Supernatants were collected, mixed with 20 μl anti-FLAG M2-agarose (Sigma), and incubated overnight at 4° C. The M2-agarose was collected from the reaction mixture by centrifugation at 5,000 rpm, 4° C. for 3 min, washed three times with CoIP washing buffer, resuspended in 75 μl of 100 ng μl⁻¹ FLAG peptide, incubated at 4° C. for 1 h, and centrifuged at 13,000 rpm for 5 min to collect the supernatant for storage at −20° C. Alternatively, the washed M2-agarose was mixed with 75 μl loading buffer, boiled at 100° C. for 5 min and stored at −20° C.

Direct Isolation of FLAG-Tagged ExoR_(c20)-CF from S. Meliloti Periplasm

Overnight culture of S. meliloti exoR95 (pHC630) was diluted 1:100 in 1 liter of fresh LB/MC/spectinomycin, and further incubated at 30° C. with shaking to an OD600 of 0.3. Cells were collected, washed twice in TBS (20 mM Tris, 0.2 mM NaCl, pH 7.5), resuspended in TBS with 0.5 M sorbitol for 10 min at room temperature, collected by centrifugation, resuspended in sterile water for 10 min on ice, and removed by two consecutive centrifugations (10 min each, 13,000 rpm). The cell-free supernatant was mixed with HEPES buffer (40 mM HEPES, 500 mM NaCl, 4% Triton X-100, pH 7.0), mixed with 60 μl agarose beads covalently linked to FLAG-specific monoclonal antibody (Sigma A2220) following the manufacturer's instructions, and incubated at 4° C. overnight with gentle inversion of the microcentrifuge tube. Agarose beads were collected at 10,000 rpm for 1 min, washed six times with TBS buffer (50 mM Tris, 0.2 mM NaCl, pH 7.5), rinsed once with 0.5 ml 0.1M glycine-HCl (pH 3.5), resuspended in 30 μl SDS-PAGE loading buffer, boiled for 5 min, and run on a 15% SDS-polyacrylamide gel at constant 150 V for 1.5 h using the Bio-Rad gel system.

Protein N-Terminal Determinations by MS-Based Peptide Mapping

In-gel digestion of excised gel bands. Following visualization of the gel, the protein band of interest was excised and placed into a 0.5-ml microtube for subsequent in-gel digestion with trypsin and manual extraction, both performed following a protocol from. All gel-extracted supernatants were combined and evaporated to dryness in a Speedvac.

Protein identification and peptide mapping by nanoLC/MS/MS analysis. The trypsin-digested samples were reconstituted in 15 μl of 0.1% (v/v) formic acid with 2% (v/v) acetonitrile prior to MS analysis. NanoLC was carried out in an LC Packings Ultimate integrated capillary HPLC system equipped with a Switchos valve switching unit (Dionex, Sunnyvale, Calif.). The gel-extracted peptides were injected using a Famous auto sampler onto a C18 PepMap trap column for on-line desalting, and then separated on a PepMap C-18 RP nano column, eluted in a 60-min gradient of 5% to 40% acetonitrile in 0.1% formic acid at 275 nl min⁻¹. The nanoLC was connected in-line to a hybrid triple quadrupole linear ion trap mass spectrometer, 4000 Q Trap from ABI/MDS Sciex (Farmingham, Mass.), equipped with Micro Ion Spray Head II ion source.

Data acquisition from the MS was performed using Analyst 1.4.2 software (Applied Biosystems) in positive ion mode for information-dependent acquisition (IDA) analysis. For the IDA analysis, after each survey scan from m/z 375 to m/z 1550 and an enhanced resolution scan, the three highest-intensity ions with multiple charge states were selected for tandem MS (MS/MS) with rolling collision energy applied for detected ions based on different charge states and m/z values.

Data analysis. The MS/MS data generated from nanoLC/ESI-based IDA analysis were submitted to Mascot 2.2 for database searching using an in-house licensed Mascot local server and the search was performed to query the SwissProt database (taxonomy: Proteobacteria) with one missed cleavage site by semi-trypsin allowed. The peptide tolerance was set to 1.5 D and MS/MS tolerance was set to 0.6 D. Carbabamidomethyl modification of cysteine and oxidation of a methionine were set as variable modifications. Only significant scores for the peptides defined by Mascot probability analysis (www.matrixscience.com/help/scoring_help.html#PBM) greater than “identity” were considered for the peptide identification.

Construction of ExoR_(c20)-Expressing Plasmid

To construct a translational fusion of the exoR signal peptide and the ExoR C-terminal proteolytic product (ExoR_(c20)), the exoR signal peptide coding region along with the exoR promoter region and the ExoR_(c20) (amino acids 81-268) coding region were obtained individually from two PCRs. The primers used to amplify the coding region for exoR promoter and ExoR signal peptide were exoRfHindIII-1 and exoR90w241r, and those to amplify the coding region for ExoR_(c20) were exoR90w241f and exoRrXhoI-2. After PCR and purification, the two fragments were ligated together via recombinant PCR using primers exoRfHindIII-1 and exoRrXhoI-2. This PCR product was then purified and digested with restriction enzymes HindIII and XhoI, and ligated with the vector pMB393 digested with the same enzymes to generate plasmid pHC567.

Construction of Plasmids Expressing ExoR Protein with Single-Amino Acid Mutations

Single-amino acid mutations of ExoR were introduced via PCR site-directed mutagenesis. To construct pHC571 with the ExoR L81A mutation, two separate PCRs were run using primer pairs exoRfHindIII-1/exoRL81Ar and exoRL81Af/exoRrXhoI-2, and plasmid pHC510 DNA as template. Primers exoRL81Ar and exoRL81Af introduced a codon change resulting in an L-to-A mutation at position 81 of the ExoR protein. The two PCR DNA fragments were ligated together via recombinant PCR using primers exoRfHindIII-1 and exoRrXhoI-2. This PCR product was then purified and digested with restriction enzymes HindIII and XhoI, and ligated with vector pMB393 digested with the same enzymes to generate plasmid pHC567.

Using a similar approach, plasmid pHC572 was constructed with the W79A mutation created by primers exoRW79Ar and exoRW79Af, and pHC573 was constructed with the Y87A mutation created by primers exoRY87Ar and exoRY87Af.

Results Extra Protein Bands in ExoR Profiles

The ExoR protein autoregulates its own expression through the ExoS/ChvI system and it has been shown to exist in the 29-kD precursor form (ExoR_(p)) and the 26-kD active mature form (ExoR_(m)) without signal peptide (FIG. 4). The ExoR_(m) form most likely interacts directly with the sensing domain of ExoS in the periplasm to regulate ExoS sensor activity. This would suggest that the amount of ExoR_(m) is linked to the activity of ExoS and that this amount needs to be tightly regulated, perhaps by converting it into an inactive form. To find other possible forms of ExoR, ExoR polyclonal antibodies were prepared by using gel-purified N-terminal-labeled His-ExoR. When total cellular proteins from S. meliloti wild-type strain Rm1021 were resolved and probed with our ExoR polyclonal antibodies, three extra prominent protein bands of 20, 21, and 24 kD were detected, in addition to the known 29-kD ExoR_(p) and 26-kD ExoR_(m) (FIG. 5). To determine the origin of the 20-, 21- and 24-kD proteins, the ExoR profile of the wild-type strain was compared to that in the loss-of-function exoR95 mutant.

The exoR95 mutant is a transposon Tn5 insertion mutant; the site of the Tn5 insertion has been genetically mapped to the end of the exoR gene. To determine the size and amino acid sequence of the ExoR95 protein, the site of the transposon insertion was determined. Tn5 was found to be inserted between codons 248 and 249, replacing the original 20 C-terminal amino acids of ExoR with a new set of 9 amino acids in the ExoR95 protein. See provisional patent application 61/652,120. This suggested that if the ExoR95 protein is synthesized and exported to the periplasm like the wild-type ExoR, it should exist in 28-kD ExoR95p and 25-kD ExoR95m forms.

Western blot analysis showed that the exoR95 mutant not only has the predicted 28-kD ExoR95p and 25-kD ExoR95m forms (FIG. 5), but also the 21- and 24-kD proteins which were found in the wild type Rm1021 cells. It is also interesting that the 20-kD protein is missing from the exoR95 mutant. The 21- and 24-kD proteins are smaller than the 25-kD ExoR95m, which makes it possible in theory for them to be derivatives of the 25-kD ExoR95m protein. Therefore, a strain with a smaller, or no ExoR protein was needed to help identify the origins of the 20-, 21-, and 24-kD proteins.

Construction of an exoR Mutant for Biochemical Analysis

After multiple attempts, we were only able to obtain one exoR mutant—exoR108, resulting from the insertion of plasmid pHC508 carrying part of the exoR open reading frame (ORF). The ExoR108 protein is predicted to be a fusion of 144 N-terminal amino acids from ExoR and 51 C-terminal amino acids from the inserted suicide plasmid (FIG. 4). The exoR108 mutant overproduced succinoglycan and formed non-swimming colonies, similar to the exoR95 mutant. These exoR108 mutant phenotypes were complemented by the plasmid pHC510 expressing wild-type ExoR protein, suggesting that the exoR108 mutation is a loss-of-function mutation (FIG. 6A and FIG. 6B).

The difficulties in obtaining an exoR mutation, and prior findings of exoR suppressor mutations in the exoS and chvI genes, prompted us to check exoS and chvI in the exoR108 mutant. Interestingly, while there was no mutation in the exoS gene, there was a single G to A nucleotide change at position 325 in the chvI gene in the exoR108 mutant. This mutation results in a change in amino acid 109 of the ChvI protein from V to M, so the exoR108 mutant is in fact an exoR108chvI109 double mutant. It was possible to transduce the exoR108 mutation from the exoR108chvI109 mutant into wild-type Rm1021 expressing the wild-type exoR gene from plasmid pHC510, but not into Rm1021 itself. This raised the possibility that the exoR gene can only be interrupted to generate the exoR108 mutation in the presence of either a plasmid-borne copy of the exoR gene or the chvI109 mutation. These findings suggest that it would not be possible to rule out the possibility that the chvI109 mutation could contribute to the phenotype of the exoR108chvI109 double mutant, and the mutant could therefore only be used for biochemical analyses of ExoR proteins in this study.

A Novel 20-kD Form of the ExoR Protein

Three proteins at 29, 26, and 20 kD stood out clearly in the ExoR protein profiles of the exoR108chvI109 double mutant with plasmid pHC510 expressing wild-type ExoR protein while the intensity of 21- and 24-kD bands remained the same as the exoR108chvI109 double mutant without plasmid pHC510 (FIG. 5). The positions of 29, 26, and 20 kD proteins matched those of the three protein bands in wild-type strain Rm1021 (FIG. 5). Since the 21- and 24-kD proteins were present in wild-type Rm1021 as well as in the exoR95 and exoR108 mutants, they are most likely nonspecific proteins. Together, these findings suggest that the ExoR protein exists in three different forms, 29, 26, and 20 kD. The finding of the previously unknown 20-kD ExoR protein suggests that ExoR could be the target of proteolysis.

ExoR_(m) is Digested in the Periplasm

The 20-kD ExoR protein, designated ExoR_(c20), could be the proteolysis product of either ExoR_(p) in the cytoplasm or ExoR_(m) in the periplasm. To find a way to restrict ExoR in either the cytoplasm or periplasm, the role of its signal peptide was further examined. The entire ExoR protein (ExoR_(p)), ExoR without the signal peptide (ExoR_(m)), and the ExoR signal peptide were separately fused to PhoA (FIG. 7A). The presence of the signal peptide was sufficient for ExoR-PhoA fusion and PhoA to be exported to the periplasm, where it displayed phosphatase activity as indicated by the blue color of the colonies on medium containing XP (5-bromo-4-chloro3-indolyl phosphate) (FIG. 7B). In the absence of signal peptide, the ExoR_(m) PhoA fusion protein remained inside the cells as indicated by the white color of the colonies (FIG. 7B).

To help determine the site of ExoR_(m) proteolysis, wild-type ExoR and ExoR_(m) were expressed in the exoR95 mutant from plasmids pHC518 and pHC641 to deliver ExoR_(m) to the periplasm or cytoplasm, respectively. When wild-type ExoR was expressed in the exoR95 mutant from plasmid pHC518, all three forms of the wild-type ExoR: ExoR_(p), ExoR_(m), and ExoR_(c20), were clearly visible, in addition to ExoR95p and ExoR95m (FIG. 7C). In contrast, when ExoR_(m) was expressed in the exoR95 mutant from plasmid pHC641, the ExoR_(m) protein as well as ExoR95p and ExoR95n, were found, but very little ExoR_(c20) protein was detected. This suggests that ExoR_(m) is very ineffectively processed inside the cytoplasm. Taken together, these findings suggest that ExoR_(m) is digested efficiently in the periplasm to yield the 20-kD form. This conclusion was further confirmed by direct isolation and sequencing of the ExoR proteolysis product from the periplasm, as described below.

Functional Analyses of C-Terminal FLAG-Tagged ExoR Protein

To determine whether the 20 kD form of ExoR shares the same C-terminus with ExoR_(m), ExoR-CF, an ExoR with an 8-amino acid C-terminal-FLAG tagged ExoR (see provisional patent application 61/652,120), was generated by fusing the FLAG tag to the ExoR C terminus (FIG. 4). ExoR-CF was expressed from plasmid pHC630 with the native exoR promoter. Our results showed that ExoR-CF was as effective at complement the succinoglycan-overproduction phenotype of the exoR95 mutant as the wild-type ExoR protein expressed from plasmid pHC510 (FIG. 6A). Similarly, ExoR-CF was as effective as the wild-type ExoR in restoring swimming activity (FIG. 6B) and nodulation of alfalfa plants of the exoR95 mutant, as determined by the percentage of pink nodules (FIG. 6C). These findings suggest that the biochemical analysis of ExoR-CF should reflect the properties of the wild-type ExoR protein.

The C Terminus of the 20-kD Form of ExoR

The C terminus of the 20 kD form of ExoR could be determined by identifying which form of ExoR protein retains the FLAG tag. Total proteins from the exoR95 mutant expressing ExoR and ExoR-CF proteins from plasmids pHC510 and pHC630, respectively, were prepared, immunoprecipitated with FLAG-specific monoclonal antibody, and probed with either our ExoR polyclonal antibodies (FIG. 8A) or the FLAG-specific monoclonal antibody (FIG. 8B). Wild-type ExoR protein without a FLAG tag could not be precipitated with the FLAG-specific antibody so it was not detected by either antibody. Our analysis of C-terminal FLAG-tagged ExoR-CF showed that all three different forms of ExoR were detected by both ExoR and FLAG antibodies (FIGS. 8A and 8B). This suggests that ExoR_(p), ExoR_(m) and ExoR_(c20) were all carrying the FLAG tag. Altogether, these findings suggest that the 20-kD form of ExoR derives from the C-terminal side of the ExoR protein (hence its designation as _(ExoRc20)).

The N Terminus of the 20-kD ExoR Fragment and the Site of ExoR Proteolysis

To identify the N-terminal amino acid of ExoR_(c20), which is also the site of ExoR proteolysis, the C-terminal FLAG-tagged ExoR-CF proteins were isolated directly from the periplasm of S. meliloti cells using osmotic shock and immunoprecipitation with commercial monoclonal FLAG-tag antibody. ExoR_(c20)-CF, ExoR_(c20) with C-terminal FLAG tag, was first isolated directly from a crude preparation of periplasmic proteins by immunoprecipitation, then resolved by SDS-PAGE, transferred to a (PVDF) membrane, and stained with Coomassie blue. A piece of membrane containing ExoR_(c20)-CF was used to identify its N-terminal amino acid by peptide mapping.

The results of the peptide mapping showed that the N-terminal amino acid of ExoR_(c20)-CF is L, and that it is amino acid 81 in the ExoR protein. The confidence in this finding was measured with Mascot probability analysis (www.matrixscience.com/help/scoring_help.html#PBM). A Mascot value of 59 represents 99% confidence. The Mascot value for L as the N-terminal amino acid was 94, indicating more than 99% confidence in the identification. Interestingly, amino acids 84, 85, 86 and 87 were also identified as N-terminal amino acids with Mascot value, ranging between values of 85 and 111. This suggested that ExoR proteolysis could take place between amino acids 80 and 87 of the ExoR protein to yield a mixture of 181 to 188 amino acid long peptides (FIG. 4). These peptides could be the result of a single digestion between amino acid 80 and 81 followed by additional digestion, or they could be the result of a single random digestion within the region of amino acid 80 to 87. The preparation method for peptide mapping used here precluded us from determining which fragment was the dominant form. Taken together, these findings suggest the strong likelihood of ExoR_(m) protein being further digested between amino acids 80 and 87 to yield ExoR_(c20) a set of 181 to 188 amino acid (19.9 to 20.6-kD) peptides.

A large number of ExoR orthologs have been discovered through genome sequencing, although few of them have been characterized in detail. Sixteen ExoR orthologs were aligned based on their overall amino acid identity, ranging from 97% to 51% (FIG. 9). Despite the dramatic decrease in the overall amino acid identity, however, the amino acid sequence around the ExoR proteolysis sites remains highly conserved among the ExoR orthologs (FIG. 9). This raises the possibility that ExoR proteolysis is conserved among other ExoR orthologs, and that proteolysis could be a common molecular signaling mechanism for ExoR proteins in different bacteria.

ExoR_(c20) does not Function in the ExoS/ChvI System

The discovery that both ExoR_(m) and ExoR_(c20) are stably maintained in the wild-type Rm1021 cells, and that ExoR_(c20) is absent in the loss-of-function exoR95 mutant, raised the possibility that ExoR_(c20) is the functional form of the protein. To examine the function of ExoR_(c20) directly, the longest form of ExoR_(c20) with 188 amino acids was fused to the 30-amino-acid ExoR signal peptide to generate SP-ExoRao expressed from pHC567. When total proteins from the exoR108chvI109 mutant expressing SP-ExoR_(c20) were probed with ExoR polyclonal antibodies, both SP-ExoR_(c20) and ExoR_(c20) were detected (FIG. 10A). This suggests that SP-ExoR_(c20) is expressed, processed, and stably maintained without its signal peptide in the periplasm.

To test the function of ExoR_(c20), the SP-ExoR_(c20) protein was expressed in the wild-type strain Rm1021 and the exoR95 mutant. The presence of the SP-ExoR_(c20)-expressing plasmid pHC567 did not change either succinoglycan or swimming phenotypes for either wild-type Rm1021 or the exoR95 mutant (FIGS. 10C and 10D). These results, along with the finding that the wild-type ExoR protein was able to complement the phenotypes of the exoR95 mutant (FIG. 5), suggest that the ExoR proteolysis product, ExoR_(c20), does not function in regulating the production of succinoglycan or flagella.

ExoR Proteolysis and Regulatory Functions are Altered by Point Mutations

Our finding of functional ExoR_(m) and nonfunctional ExoRe20 co-existing in the periplasm raised the possibility that the amount of ExoR_(m) is maintained at a certain level and that any changes to the level of ExoR_(m) will alter the function of the ExoR protein. To test this possibility, two highly conserved amino acids at positions 79 and 81, and one nonconserved amino acid at position 87 were changed individually to A (alanine) (FIG. 4). When these three mutant ExoR proteins, ExoRW79A, ExoRL81A, and ExoRY87A, were expressed from plasmids pHC571, pHC572, and pHC573, respectively, in the exoR108chvI109 double mutant, the level of the ExoR_(m) form was significantly reduced for the ExoRL81A mutant, slightly reduced for the ExoRW79A mutant, but not changed for the ExoRY87A mutant (FIG. 11A). These suggest that the L81A mutation may have reduced the amount of ExoR_(m) form of ExoR mutant protein in the cells.

The regulatory functions of the three mutated ExoR proteins were examined by assessing their abilities to complement the succinoglycan-producing (represented by calcofluor brightness) and non-swimming phenotypes of the exoR95 mutant (FIGS. 11C, 11D). Compared to the wild type ExoR protein, the ExoRL81A protein was not able to complement neither succinoglycan producing nor non-swimming phenotypes of the exoR95 mutant, and it is therefore a loss-of-function mutation. Both ExoRW79A and ExoRY87A proteins partially complemented both succinoglycan producing and non-swimming phenotypes of the exoR95 mutant. The ExoRY87A was more effective than ExoRW79A in complementing the succinoglycan producing phenotype. These results suggest that both ExoRW79A and ExoRY87A are functional and that ExoRY87A is more effective than ExoRW79A but less effective than wild type ExoR.

The combined biochemical and functional analyses of the three mutant ExoR proteins suggest that the level of ExoR_(m) is linked to the regulatory function of ExoR protein. This raises the possibility that ExoR proteolysis can be modulated by environmental or plant signals to regulate the production of succinoglycan, flagella, and many other cellular products required for symbiosis.

DISCUSSION

Recent publications have shown that S. meliloti ExoR protein most likely functions as the repressor of the ExoS sensor, as part of the ExoR autoregulation pathway, which allows it to indirectly regulate the expression of a large number of genes required for host invasion and symbiosis. Both genetic and biochemical data appear to support the model that ExoR interacts with ExoS periplasmic sensing domain directly to suppress ExoS, keeping it in an off state. It follows that ExoR suppression of ExoS would have to be relieved during nodulation so that the expression of the invasion and symbiosis genes could be turned on to support the nodulation. However, the molecular mechanism mediating the release of ExoR suppression of ExoS is not clear.

One simple and attractive model for the relief of ExoR suppression is a reduction in the amount of ExoR protein in its mature and active form, ExoR_(m), by changing it to an inactive form through proteolysis or modification. To monitor such changes in ExoR_(m) on a western blot, antibodies are required that can recognize the entire ExoR protein and a S. meliloti strain to provide the genetic background with no ExoR protein. While generating ExoR-specific polyclonal antibodies was relatively straightforward, engineering a S. meliloti strain with no ExoR proved to be challenging.

Two complementary approaches were followed to find a clean background for the analysis of ExoR protein. The first was to determine the status of ExoR in the original loss-of-function exoR95 mutant. Our analysis showed that the mutated ExoR95 protein can be easily found in two forms ExoR95p and ExoR95m. This makes it more difficult to monitor the changes in wild-type ExoR protein since these two forms are just slightly smaller than the wild type, as predicted based on the site of the exoR95 mutation. The second approach, which was to generate an ExoR-deletion mutation, turned out to be much more difficult. The only new exoR mutation generated from this effort was the exoR108chvI109 double mutant with a plasmid insertion in the exoR gene. The exoR108 mutation can be transduced from the exoR108chvI109 double mutant into wild-type strain Rm1021 (pHC510) expressing exoR gene from plasmid pHC510, but not into Rm1021 alone. This suggests that the presence of a chvI109 mutation is likely to be essential for the existence of the exoR108 mutation in the S. meliloti genome. This led us to decide that even though the succinoglycan- and flagellum-production phenotypes of the exoR108 mutant can be complemented by the wild-type exoR gene, the exoR108chvI109 mutant would only be used for biochemical analysis of the ExoR protein in this study.

Our comparative analysis of the ExoR protein profiles in a different genetic background led to the discovery of a new form of ExoR protein, ExoR_(c20), while confirming the existence of the ExoR and ExoR_(m) forms. Two lines of evidence suggest that ExoR_(c20) is the periplasmic proteolysis product of ExoR_(m). The first is that when ExoR_(c20) was sequestered inside the cytoplasm by removing its signal peptide, no ExoR_(c20) was detected. The second is the direct isolation of ExoR_(c20) from the periplasm. While ExoR_(c20) has a single C terminus, which is the same as that of wild-type ExoR, it appears to have multiple N termini. When a gel-purified single ExoR_(c20) protein band was used for N-terminus mapping, the results demonstrated N termini at positions 81, 84, 85, 86 and 87 of the ExoR ORF. These fragments may be produced by one or multiple enzymes in parallel, or produced by one specific endoprotease digestion followed by multiple exoprotease digestions. While further analysis of these proteolysis products is important to identify the protease involved in ExoR_(m) proteolysis, the more important finding of this study is the fact that ExoR_(m) is the subject of proteolysis. This could serve as the molecular mechanism that reduces the active ExoR_(m), and releases suppression of the ExoS sensor.

The presence of stably maintained ExoR_(c20) in wild-type Rm1021 but not in the loss-of-function exoR95 mutant raised the question of whether ExoR_(c20) functions in the ExoR-ExoS/ChvI signal-transduction pathway. To address this question, the longest form of ExoR_(c20) was fused directly to the ExoR signal peptide and expressed in the wild-type Rm1021 and the exoR95 mutant. The presence of ExoR_(c20) in both strains was confirmed by western blot. The presence of ExoR_(c20) did not alter the succinoglycan and swimming phenotypes of either the wild type or the exoR95 mutant. This suggests that ExoR_(c20) does not play any significant role in regulating succinoglycan or flagellum production. More importantly, it also suggests that digesting ExoR_(m) to ExoR_(c20) might function as a molecular mechanism regulating the amount of ExoR_(m) in the periplasm.

For proteolysis of ExOR_(m) to serve as a mechanism regulating the function of ExoR, modulation of the amount of ExoR_(m) should change the regulatory function of ExoR. To test this hypothesis, the highly conserved amino acid leucine (L) at the site of the proteolysis was changed to alanine (A), generating ExoRL81A. In addition, similar site-directed mutations were generated for another conserved amino acid, giving ExoRW79A, and a nonconserved amino acid, giving ExoRY87A. The mutation of the nonconserved amino acid 87 showed no detectable change in the levels of ExoR_(m) protein or the regulatory function of ExoR. Compared to the wild type ExoR, the ExoRW79A mutation of the conserved W (tryptophan) slightly decreased ExoR_(m) level and slightly reduced the regulatory function of ExoR. The ExoRL81A mutation, which changes the proteolysis site (amino acids 80-81), dramatically decreased the amount of ExoR_(m) protein and completely abolished the regulatory function of the ExoR protein. Altogether, these findings link reduction of ExoR_(m) and the regulatory function of the ExoR protein. In addition, our finding of single amino acid change, the L81A mutation, enhancing ExoR_(m) proteolysis raises the possibility that the ExoR proteolysis sequence is fine-turned for optimum control of proteolysis instead of efficient proteolysis. The better control of ExoR_(m) proteolysis will allow S. meliloti cells to sense and react more effectively to the presence of yet to identified host or environmental signals.

A model is proposed to integrate the new findings from this study with those from previous work (FIG. 12). We propose that the newly synthesized precursor form of ExoR, ExoR_(p), is directed to the membrane and secreted into the periplasm without its signal peptide, to form the mature ExoR_(m). The amount of periplasmic ExoR_(m) in free-living S. meliloti cells is kept in equilibrium by both interaction with ExoS and its steady proteolysis, forming ExoR_(c20). This model is supported by previous results (5, 33, 53, 55) and our finding that the point mutation L81A reduces the level of ExoR_(m) and disables the regulatory function of the ExoRL81A protein. The ExoR95 mutant protein might have an altered conformation such that it is resistant to proteolysis and thus no proteolytic product, ExoR95_(c19), equivalent of ExoR20, is detectable, or that the resulting ExoR95c19 is not stable.

Our model would predict that plant or environmental signals would alter the rate of ExoR_(m) proteolysis, thereby changing the level of ExoR suppression of ExoS. This would allow S. meliloti cells to modulate the production of succinoglycan and flagella, as well as the expression of many other ExoR-ExoS/ChvI pathway-regulated genes, to support the establishment of symbiosis in response to the presence of plant host or environmental signals. Based on this prediction, we are currently screening for conditions that can change the level of succinoglycan production by the wild type Rm1021.

Close homologs of ExoR, as well as of ExoS and ChvI of the ExoR-ExoS/ChvI signal-transduction pathway have been found in the genomes of more than 40 different bacterial species. The regulatory mechanisms and the genes regulated by these systems are, with a few exceptions, unknown. When ExoR homologs are aligned in order of decreasing overall homology from 93% to 50% to the S. meliloti ExoR protein, the levels of homology around the region of proteolysis remain unchanged. The high levels of conservation of protein sequence around the ExoR_(in) proteolysis region raises the possibility that ExoR proteolysis is a common molecular mechanism mediating bacterial sensing in the presence of their hosts or of changes in their environment.

Bacterial periplasmic proteases have been shown to participate in bacterial sensing of environmental signals in several systems. An Escherichia coli membrane-bound protease, DegS, which is activated by unassembled outer-membrane porins, cleaves the periplasmic domain of the membrane-anchored regulator, RseA. This triggers further cleavage of RseA by a metalloprotease, YaeL, to release σ^(E), which normally attaches to RseA. The free σ^(E) turns on the expression of stress-related genes. In the case of a polarity determinant of Caulobacter, PodJ, the periplasmic domain of PodJ is also regulated through cleavage into small fragments by a periplasmic protease, PerP. The example that is closest to S. meliloti ExoR is the function and regulation of the E. coli periplasmic adaptor protein, CpxP, which is involved in sensing pH variations to regulate membrane lipid composition. The CpxP protein interacts with and inhibits the periplasmic sensing domain of the CpxA protein, the sensor of the CpxA/CpxR two-component system. The periplasmic serine protease, DegP, is activated by general envelope disruptions, including pH changes, and cleaves the CpxP protein, thereby removing CpxP from the CpxA sensor. This results in the activation of CpxA sensor and the expression of its regulated genes. Our finding that ExoR is the subject of proteolysis in the periplasm suggests a regulatory role similar to that of RseA, PodJ and CpxP.

While it has been well documented that ExoR, ExoS, and ChvI play essential roles in symbiosis, it is not known what environmental signals are transmitted through the ExoR-ExoS/ChvI signal-transduction pathway. The factors that might function upstream of ExoR are also unknown. Our finding of ExoR proteolysis in the periplasm suggests a protease(s) as a key factor upstream of ExoR. The proteolysis of ExoR might be regulated by other proteins in the periplasm through protein-protein interactions or by other enzymes that modify ExoR. These possibilities will be further investigated to gain more insight into the regulation of ExoR and the function of the ExoR-ExoS/ChvI signal-transduction pathway. The results of our analysis of ExoR will no doubt be helpful in understanding and combating the pathogenicities of A. tumefaciens and B. abortus, as well as many other host-interacting bacteria that rely on homologs of the ExoR-ExoS/ChvI signal-transduction pathway.

This written description uses examples to disclose the invention, including the best mode, and also to enable any person skilled in the art to practice the invention, including making and using any devices or systems and performing any incorporated methods. The patentable scope of the invention is defined by the claims, and may include other examples that occur to those skilled in the art. Such other examples are intended to be within the scope of the claims if they have structural elements that do not differ from the literal language of the claims, or if they include equivalent structural elements with insubstantial differences from the literal language of the claims. 

What is claimed is:
 1. A method for modulating a bacterial invasions switch by changing the proteolysis of ExoR protein, the method comprising administering a protease inhibitor to a bacterium such that proteolysis of the mature form of ExoR_(m) is inhibited thereby keeping the bacterium in a non-pathogenic state, wherein the protease inhibitor is an organic sulfonylfluoride inhibitor with a structure consistent with:

wherein R₁ is selected from a group consisting of an arene; a substituted arene; a lipid with at least three carbons but fewer than one hundred carbons; a nucleic acid and an amino acid.
 2. The method as recited in claim 1, further comprising quantifying a first ExoR_(m) level after the step of administering wherein the first ExoR_(m) level is lower than a second ExoR_(m) level prior to the step of administering.
 3. The method as recited in claim 1, further comprising testing the bacterium to verify the bacterium is in the non-pathogenic state, the testing being performed after the step of administering.
 4. The method as recited in claim 1, further comprising introducing the bacterium to an animal, the step of introducing being performed after the step of administering.
 5. The method as recited in claim 1, further comprising introducing the bacterium to a plant, the step of introducing being performed after the step of administering.
 6. The method as recited in claim 1, further comprising exposing the bacterium to a cell penetration agent, the step of exposing being performed prior to the step of administering.
 7. The method as recited in claim 1, wherein R₁ is a nucleic acid selected from adenine, cytosine, guanine, thymine, uracil and combinations thereof.
 8. The method as recited in claim 1, wherein R₁ is a polynucleic acid with more than one, but fewer than one hundred, nucleic acids residues.
 9. The method as recited in claim 1, wherein R₁ is a positively charged amino acid.
 10. The method as recited in claim 1, wherein R₁ is a negatively charged amino acid.
 11. The method as recited in claim 1, wherein R₁ is a polar amino acid.
 12. The method as recited in claim 1, wherein R₁ is a hydrophobic amino acid.
 13. The method as recited in claim 1, wherein R₁ is an amino acid selected from the group consisting of cysteine, glycine, proline and selenocysteine.
 14. The method as recited in claim 1, wherein R₁ is a polypeptide with more than one, but fewer than one hundred, amino acid residues.
 15. The method as recited in claim 1, where R₁ is a substituted arene with the structure of:

wherein each of R₂ to R₆ are independently selected from the group consisting of a carbohydrate; H; OH; F; SH; CH₃(CH₂)_(n)S; CH₃(CH₂)_(n); NH₂(CH₂)_(n); wherein n is an integer between zero and three.
 16. A method for modulating a bacterial invasions switch by changing the proteolysis of ExoR protein, the method comprising administering a protease inhibitor to a bacterium such that proteolysis of the mature form of ExoR_(m) is inhibited thereby keeping the bacterium in a non-pathogenic state, wherein the protease inhibitor is selected from the group consisting of a serpin inhibitor, alpha-1 antitrypsin, alpha-2 antiplasmin, antithrombin, methoxy arachidonyl fluorophosphonate, C1-inhibitor, conspin, CU-2010, CU-2020, Maspin, Protein C inhibitor, Protein Z-related protease inhibitor, camostat.
 17. A method for modulating a bacterial invasions switch by changing the proteolysis of ExoR protein, the method comprising administering a protease inhibitor to a bacterium disposed in an aqueous medium such that proteolysis of the mature form of ExoR_(m) is inhibited thereby keeping the bacterium in a non-pathogenic state, wherein the protease inhibitor is a substrate that increases aqueous medium pH or the protease inhibitor is an alkali metal or an alkaline earth metal present in a concentration of at least 2 mM.
 18. The method as recited in claim 17, wherein the protease inhibitor is calcium present in a concentration of at least 2 mM.
 19. The method as recited in claim 17, wherein the protease inhibitor is sodium present in a concentration of at least 150 mM.
 20. The method as recited in claim 17, wherein the aqueous medium pH is between 6 and
 7. 